RESEARCH
Mosaic RNA Phage VLPs Carrying Domain III of the West NileVirus E Protein
Indulis Cielens • Ludmila Jackevica •
Arnis Strods • Andris Kazaks • Velta Ose •
Janis Bogans • Paul Pumpens • Regina Renhofa
� Springer Science+Business Media New York 2014
Abstract The virus-neutralising domain III (DIII) of the
West Nile virus glycoprotein E was exposed on the surface
of RNA phage AP205 virus-like particles (VLPs) in mosaic
form. For this purpose, a 111 amino acid sequence of DIII
was added via amber or opal termination codons to the
C-terminus of the AP205 coat protein, and mosaic AP205-
DIII VLPs were generated by cultivation in amber- or opal-
suppressing Escherichia coli strains. After extensive puri-
fication to 95 % homogeneity, mosaic AP205-DIII VLPs
retained up to 11–16 % monomers carrying DIII domains.
The DIII domains appeared on the VLP surface because
they were fully accessible to anti-DIII antibodies. Immu-
nisation of BALB/c mice with AP205-DIII VLPs resulted
in the induction of specific anti-DIII antibodies, of which
the level was comparable to that of the anti-AP205 anti-
bodies generated against the VLP carrier. The AP205-DIII-
induced anti-DIII response was represented by a significant
fraction of IgG2 isotype antibodies, in contrast to parallel
immunisation with the DIII oligopeptide, which failed to
induce IgG2 isotype antibodies. Formulation of AP-205-
DIII VLPs in alum adjuvant stimulated the level of the anti-
DIII response, but did not alter the fraction of IgG2 isotype
antibodies. Mosaic AP205-DIII VLPs could be regarded as
a promising prototype of a putative West Nile vaccine.
Keywords West Nile virus E glycoprotein � Domain
DIII � RNA phage AP205 � Mosaic � Virus-like particles
Introduction
West Nile virus (WNV) is a neurotropic, single-stranded
and positive-sense RNA flavivirus that is transmitted to
humans through the bite of an infected mosquito and has
emerged globally as a significant cause of viral encephalitis
(for recent reviews see [1, 2]). In the absence of a specific
anti-viral treatment, the development of a safe and an
efficient prophylactic vaccine against WNV is necessary.
Currently, most WNV vaccine candidates are live,
attenuated viral vaccines based on chimeric viruses that
incorporate the pre-membrane (prM) and E glycoproteins
of the WNV envelope into the following viral vectors:
yellow fever [3–6], fowlpox and canarypox [7], measles [8]
and the modified vaccinia virus Ankara (MVA) strain of
vaccinia virus [9]. The generation and preclinical efficacy
of a hydrogen peroxide-inactivated WNV vaccine has been
described [10]. A DNA vaccine encoding the prM and E
proteins have been evaluated in healthy adults [11].
Recombinant subunit vaccine candidates are based on
the structural WNV glycoprotein E because the protein
may elicit a major neutralising antibody response [12, 13].
The recombinant E protein was purified from Escherichia
coli and functioned as an efficient WNV vaccine in mice
[14]. The WN-80E subunit vaccine, which is produced in a
Drosophila melanogaster expression system, consists of
the recombinant E protein truncated at the C-terminal end
but contains 80 % of its N-terminal amino acids (aa) [15–
17]. Recently, recombinant baculoviruses expressing WNV
E protein, as well as prM protein, were constructed and
tested successfully in mice [18, 19].
Within the E glycoprotein, domain III (DIII) is the region
that is exposed on the viral surface [20] and is implicated in
receptor binding [21]. DIII is a target of the most WNV
neutralising antibodies [22–26], and passive transfer of DIII-
I. Cielens � L. Jackevica � A. Strods � A. Kazaks � V. Ose �J. Bogans � P. Pumpens (&) � R. Renhofa (&)
Latvian Biomedical Research and Study Centre, Ratsupites
Street 1, Riga 1067, Latvia
e-mail: [email protected]
R. Renhofa
e-mail: [email protected]
123
Mol Biotechnol
DOI 10.1007/s12033-014-9743-3
specific antibodies may protect mice from WNV challenge
[27]. Subunit vaccines based on recombinantly expressed
DIII have been tested in animal models and have proven
effective in protecting against WNV infection [28–32].
The immunogenicity of DIII was strongly enhanced by
chemical conjugation to virus-like particles (VLPs) of the
bacteriophage AP205 [33], in accordance with the general
acceptance of VLPs as highly ordered carriers for foreign
epitopes (for recent reviews see [34, 35]).
In the present study, construction of a novel type of
putative VLP-based DIII vaccine is described. RNA bac-
teriophage AP205 VLPs [36] are used to expose the DIII
sequence on the mosaic VLPs. In contrast to the previous
chemically conjugated vaccine [33], mosaic AP205 VLPs
are generated by genetic fusion of the DIII sequence to the
C-terminus of the AP205 coat protein (CP) via the termi-
nation codons UAG and UGA under codon-suppression
conditions. Uniform fusions of the DIII sequence, without
any read-through termination codons, to AP205 CP as well
as to the CP of a similar RNA bacteriophage, GA, do not
lead to self-assembly and formation of VLPs. Direct
expression of the DIII sequence is used as a source of the
highly purified recombinant DIII protein. Overall, we
present efficient production and purification of mosaic
AP205-DIII VLPs in E. coli cells and show the ability of
mosaic VLPs to induce specific anti-DIII antibodies in
mice.
Materials and Methods
Bacterial Strains
Escherichia coli strain RR1 [F- rB- mB- leuB6 proA2 thi-1
araC14 lacY1 galK2 xyl-5 mtl-1 rpsL20 (Strr) glnV44 D(mcrC-mrr)] was used for the cloning and selection of
recombinant plasmids. E. coli C2566 was used for the direct
expression of the DIII gene. E. coli JM109 was used to
express the fused AP205-DIII and GA-DIII genes. For the
expression of mosaic AP205-am-DIII and AP205-op-DIII
VLPs, the amber suppressor E. coli JM109 (pISM579) and
the opal suppressor E. coli JM109 (pISM3001) carrying
resident suppressor tRNA genes were used. The plasmid
pISM3001 [37] was a kind gift from Dr. F.C. Minion (USA),
while strain MY579 harbouring amber suppressor tRNA was
obtained from Dr. M. Yarus (USA). The plasmid pISM579
encoding tRNA for amber (UAG) codon suppression was
constructed on the basis of the plasmid pISM3001, where the
opal (UGA) suppressor tRNA encoding gene trpT176 was
replaced with analogous DNA sequence encoding the Hirsh
amber suppressor tRNA. The latter was isolated from plas-
mid pBE621 [38] that encodes the trpT178 derivative,
which, in addition to Hirsh mutation G24 ? A, also contains
mutations U33 ? G and C35 ? U. Because the respective
tRNA genes are flanked by EcoRI sites, the substitution was
carried out by partial EcoRI cleavage and religation and then
confirmed by sequencing.
Construction of the WNV Protein E Domain DIII-
Expressing Plasmids
The construction map of the WNV protein E domain DIII-
expressing plasmids is shown in Fig. 1. To construct the
AP205-DIII expression units, a set of cloning vectors
(Fig. 1, on the left) was generated on the basis of a
pAP283-58 plasmid that expresses the CP gene of the RNA
bacteriophage AP205 under the control of the E. coli
tryptophan operon promoter Ptrp [36]. The following oli-
gonucleotides were used as PCR primers to insert the
sequences encoding the linker aa residues together with the
appropriate cloning sites and the suppression codons
(underlined) at the C-terminus of the AP205 CP gene:
50-TGTCTAGAATTTTCTGCGCACCCATCCCGG-30;50-TGATGCATCCTCCGGATCCAGCAGTAGTATC
AGACGATAC-30;50-TACCATGGCAAATAAGCCAATGCAACCG-30;50-GTAAGCTTAGATGCATTATCCGGATCCCTA
AGCAGTAGTATCAGACGATACG-30;50-GTAAGCTTAGATGCATTATCCGGATCCTCA
AGCAGTAGTATCAGACGATACG-30.
The WNV protein E DIII fragment encompassing aa
residues 296–406 was PCR-amplified from the plasmid
pTrcHis2-WNVclone F101 New York strain 385–399
(kindly supplied by B. E. E. Martina, Erasmus MC, Rot-
terdam) and cloned into the previously constructed vectors
at the appropriate restriction sites (Fig. 1, on the right).
The following oligonucleotides were used as cloning
primers for the PCR:
50-CATCCGGACAGTTGAAGGGAACAAC-30;50-GTATGCATTTGCCAATGCTGCTTCC-30;50-CATCCGGACAGTTGAAGGGAACAAC-30;50-GTAAGCTTATTTGCCAATGCTGCTTCC-30
To construct the GA-DIII expression units, a pGA
355-24 plasmid expressing the CP gene of the RNA bac-
teriophage GA under control of the Ptrp [39, 40] was
supplied with the appropriate linker at the C-terminus and
used as a vector for cloning of the DIII sequence amplified
with the following primers:
50-CATCCGGACAGTTGAAGGGAACAAC-30 and
50-GTAAGCTTATTTGCCAATGCTGCTTCC-30
For direct expression, the DIII sequence was amplified
by the primers
Mol Biotechnol
123
50-TACCATGGGCCAGTTGAAGGGAACAACCTAT
GG-30 and
50-ATGAAGCTTATTTGCCAATGCTGCTTCC-30
and inserted at the restriction sites NcoI and HindIII in the
multicloning region of the plasmid pET-28? under control
of the IPTG-inducible T7 promoter. The plasmid structures
were confirmed by sequencing.
Expression and Purification of AP205- and GA-DIII
Derivatives
Escherichia coli JM109 cells were transformed with the
pAP205-DIII and pGA-DIII plasmids. E. coli JM109
strains carrying resident suppressor tRNA plasmids were
used for the expression of AP205-DIII mosaics. E. coli
JM109 with a resident amber suppression tRNA gene
(pISM579) was transformed with the pAP205-am-DIII
plasmid. E. coli JM109 with a resident opal suppression
tRNA gene (pISM3001) was transformed with the
pAP205-op-DIII plasmid. Single colonies were suspended
in tubes containing 5 mL of LB medium with 50 lg/mL of
ampicillin and 10 lg/mL of chloramphenicol and grown
without shaking at 37 �C for 16 h. The prepared inoculum
was diluted tenfold in M9 medium supplemented with
10 g/L of casamino acids, 2 g/L of glucose (BD, USA),
25 lg/mL of vitamin B1, 20 mM magnesium sulphate,
ampicillin (50 lg/mL) and chloramphenicol (10 lg/mL)
grown in 3 L Erlenmeyer flasks on an Infors shaker
(200 rpm) at 37 �C to an OD540 of 0.8–1.0, induced with
100 lg/mL of IPTG and cultivated for 4 h. Cells were
harvested by centrifugation.
To purify the mosaic AP205-am-DIII and AP205-op-
DIII VLPs, 3 g of wet, fresh cells were homogenised in
9 mL of lysis buffer containing 50 mM Tris–HCl (pH 8.0),
5 mM EDTA, 50 lg/mL PMSF and 0.1 % Triton X-100
and then ultrasonicated five times for 15 s each time at
22 kHz at 45 s intervals, while keeping the cells on ice.
After centrifugation at 10,000 rpm for 30 min, the super-
natant was loaded onto a Sepharose CL-2B column
(70 9 2 cm). NET buffer [0.15 M NaCl, 20 mM Tris–HCl
(pH 7.8), 5 mM EDTA] with 0.02 % Brij58 was used for
elution at a velocity of 2 mL/h, 90 min/3-mL fraction.
VLP-containing fractions were detected by native 0.8 %
Fig. 1 Schematic representation of the recombinant DIII constructions. The nucleotide and aa sequences and the locations of restriction sites at
the joining points are shown. Undefined aa residues are depicted by X
Mol Biotechnol
123
agarose (TopVision LE GQ, Fermentas, Lithuania) gel
electrophoresis in 1xTAE buffer [40 mM Tris (pH 8.4),
20 mM acetic acid, 1 mM EDTA] (Fermentas). The VLP-
containing fractions (typically fractions 15–28) were
pooled and the material was loaded onto a Sephadex A50
(5–7 9 1 cm) column, which does not retard VLPs, to
remove nucleic acids. Unbound material containing VLPs
was washed out with NET buffer (without Brij58) under
spectrophotometric control. After concentration on an
Amicon Ultra-15 centrifugal filter device (MWCO 30,000;
Merck Millipore, USA), the samples were loaded onto a
Sepharose CL-4B column (48 9 1.5 cm) and eluted with
NET buffer at a velocity of 2 mL/h/fraction. The fractions
detected by native agarose gel electrophoresis (NAGE)
(typically fractions 17–25) were pooled, concentrated on
the Amicon device as described above, and subjected again
to gel filtration on the Sepharose CL-2B column
(60 9 1.5 cm) in NET buffer by collection of 2-mL frac-
tions. The VLP-containing fractions (typically fractions
24–33) were pooled, concentrated on the Amicon device to
3 mL, and loaded onto a pre-formed 5–36 % sucrose gra-
dient (sucrose concentration (w/w) layers: 36 % to 3 mL;
30 % to 3 mL; 25 % to 6 mL; 20 % to 8 mL; 15 % to
6 mL; 10 % to 6 mL; 5 % to 3 mL; in Polyallomer
25 9 89 mm tubes) for centrifugation in a Beckman
Coulter Optima L-100XP ultracentrifuge (rotor SW32 Ti)
at 20,500 rpm for 13 h at ?4 �C. Fractions of 1 mL were
collected from the pierced bottom of the tube. The VLPs
usually appeared around fraction 12, which was in the first
third from the bottom. Sucrose was removed by Amicon
concentrator to a volume of 1.5 mL in NET buffer and
1.5 mL of glycerol was added. VLP preparations with a
typical protein concentration of 8 mg/mL (31 OD260 units/
mL) were stored at -18 �C. The yield of VLPs reached
8 mg/g of wet cells.
To purify the GA-DIII derivative, the debris of the cell
lysate prepared as described above and centrifuged at
10,000 rpm for 30 min was eluted by 7 M urea in water
and loaded onto a DEAE cellulose column (1 9 5 cm) in
20 mM Tris–HCl (pH 8.6). The unbound material was
collected in fractions of 3 mL. The most pure fractions
were pooled, subjected to ammonium sulphate precipita-
tion at 50 % saturation, dissolved in 7 M urea and diluted
to 10 lg/mL in a 50 mM sodium carbonate buffer, pH 9.6,
for coating on ELISA plates.
Expression and Purification of the DIII Protein
Escherichia coli C2566 cells were transformed with the
pET28b-DIII plasmid (Fig. 1). Single colonies were sus-
pended in tubes containing 5 mL of LB medium with
50 lg/mL of ampicillin and grown without shaking at
37 �C for 16 h. The prepared inoculum was diluted tenfold
in 2TY medium containing 20 lg/mL of ampicillin in 2 L
flasks, incubated on an Infors shaker (200 rpm) at 37 �C to
an OD540 of 0.8–1.0, induced by adding IPTG to 100 lg/
mL and cultivated for 3.5–4.5 h. Cells were harvested by
centrifugation.
To purify the DIII protein, 1 g of cells was homogenised
and ultrasonicated in 4 mL of lysis buffer, and the super-
natant was discarded. The pellet was extracted with 4 mL
of 7 M urea in water. To remove the nucleic acids, two
alternative techniques were used: (i) proteins in the
supernatant were precipitated by adding ammonium sul-
phate to 50 % saturation for 20 h at 4 �C, the debris was
dissolved in 7 M urea and the ammonium sulphate pre-
cipitation was repeated and (ii) the supernatant was loaded
onto a DEAE cellulose column equilibrated with 20 mM
Tris–HCl (pH 8.6), and the unbound material was collected
and precipitated with ammonium sulphate at 50 % satura-
tion. The pellets obtained from both versions were washed
by water portions of 200 lL to remove any remaining
nucleic acids. After centrifugation at 10,000 rpm for
30 min, the samples were resuspended in a minimal vol-
ume of 7 M urea containing 5 mM dithiotreitol (Sigma-
Aldrich, USA), clarified by centrifugation at 6,000 rpm,
and refolded by dialysing the 3 mL sample for 3–4 days
against 4–5 changes of 50 mL of buffer containing 2 M
urea and 0.5 M arginine-HCl (pH 8.0) [41]. After clarify-
ing at 6,000 rpm for 15–20 min, the sample was subjected
to gel filtration on a Sepharose CL-4B column (30 9 1 cm)
and eluted in PBS buffer (0.01 M phosphate, pH 7.4,
0.138 M NaCl, 0.0027 M KCl) at a velocity of 1 mL/h,
90 min/1.5-mL fraction. The final samples were stored
frozen at -18 �C.
Detection of Protein and Nucleic Acids
All measurements were performed on Biochrom (Bio-
chrom Ltd., UK) and Nanodrop (Thermo Scientifics, USA)
spectrophotometers. The amount of protein (in the presence
of nucleic acids) was estimated according to [42]. The VLP
preparations were compared with respect to the presence of
protein and nucleic acids using NAGE and double radial
immunodiffusion (DRI) according to the method of
Ouchterlony using rabbit polyclonal anti-AP205 antibod-
ies. For NAGE and DRI, 1 and 0.8 % TopVision LE GQ
Agarose (Fermentas) in TBE buffer and in PBS buffer were
used, respectively, with subsequent Coomassie Blue R-250
(60 lg/mL of Coomassie Blue R-250 in 10 % acetic acid)
staining of the gels.
Protein samples were analysed on 15 % SDS-PAGE
gels with subsequent Coomassie staining. For Western
blots, the polyclonal rabbit anti-AP205 was used at a
1:1000 dilution. All chemicals were from Sigma-Aldrich.
Mol Biotechnol
123
The ratio of DIII-containing versus initial AP205 pro-
teins was determined by analysis of Coomassie-stained gels
with the free ImageJ program (http://rsbweb.nih.gov/ij/).
Electron Microscopy and Dynamic Light Scattering
Analysis
For electron microscopy, VLPs in suspension were adsor-
bed to carbon-Formvar coated copper grids and negatively
stained with a 1 % uranyl acetate aqueous solution. The
grids were examined with a JEM-1230 electron microscope
(Jeol Ltd., Tokyo, Japan) at 100 kV.
The size of the particles was detected by dynamic light
scattering (DLS) in a Zetasizer Nano ZS (Malvern Instru-
ments Ltd, UK) instrument.
Immunogenicity of the DIII-Containing Proteins
Female BALB/c mice, 6–8 weeks of age and obtained from
the Latvian Experimental Animal Laboratory (Riga Stra-
dins University), were maintained at the Biomedical
Research and Study Centre under pathogen-free conditions.
The experiments were approved by the Latvian Animal
Protection Ethics Committee and the Latvian Food and
Veterinary service, permission No. 31/23.10.2010. Groups
of five mice were immunised sub-dermally on the back of
the animals with 25 lg of protein (diluted in 0.2 mL of
PBS) per mouse on days 0, 14 and 28. For immunisation
with adjuvants, 250 lg of Alum for all three immunisations
and 100, 250 and 500 lg of SiO2 for the first, second and
third immunisation, respectively, were used. To assess the
humoral response, the animals were bled on days 7, 14 and
28, reimmunised on days 15 and 29, and sacrificed on day
42. The anti-DIII titres in the sera were determined with a
direct ELISA using plates coated with DIII protein or GA-
DIII fusion protein. The anti-AP205 titres were determined
with a direct ELISA using plates coated with the AP205
VLPs.
For the direct ELISA, 96-well microplates (Nunc, USA)
were coated with the appropriate proteins using 100 lL of
protein solution (10 lg/mL in 50 mM sodium carbonate
buffer, pH 9.6) per well. The plates were incubated with
the protein solution overnight at 4 �C. After the plates were
blocked with 1 % BSA in PBS for 1 h at 37 �C, serial
dilutions of the sera were added to the wells, and the plates
were incubated at 37 �C for an additional 1 h. After
washing three times with PBS containing 0.05 % Tween-
20, 100 lL of horseradish peroxidase conjugated anti-
mouse antibody (Sigma-Aldrich) was added at a 1:10,000
dilution. After incubation at 37 �C for 1 h, the plates were
washed, and OPD substrate (Sigma-Aldrich) was added for
colour development. A Multiskan (Sweden) was used to
measure the absorbance at 492 nm. The end-point titres
were defined as the highest serum dilution that resulted in
an absorbance value three times greater than that of the
control sera obtained from unimmunised mice.
The IgM and IgG subsets in the sera of the immunised
mice were detected with isotype specific ELISAs using a
mouse monoclonal antibody isotyping reagent and an anti-
goat/sheep IgG peroxidase conjugate (Sigma-Aldrich).
For the competitive ELISA, 96-well microplates were
coated with the DIII protein using 100 lL of protein
solution (10 lg/mL) per well. After the plates had been
coated, 50 lL aliquots of serial dilutions of competing
protein AP205-am-DIII and 50 lL of the anti-DIII were
added to the wells simultaneously. The 1:800 dilution of
the anti-DIII with an OD492 value within the range of
0.5–0.6 in the control samples without competing protein
was used. After incubation at 37 �C for 1 h, the micro-
plates were processed as described above. The percent
inhibition (I%) of antibody binding by the competing
protein was calculated as follows:
I% = [(OD492 test sample - OD492 negative control)/
(OD492 positive control - OD492 negative control)] 9 100.
The molar amounts of the proteins necessary for 50 %
inhibition (I50) were calculated.
Results
Construction, Expression and Purification
of Recombinant AP205 Variants Carrying the DIII
Epitope
The construction of the recombinant AP205-am-DIII and
AP205-op-DIII genes, where the DIII sequence is C-ter-
minally fused to the AP205 CP over amber or opal trans-
lation termination codons, is depicted in Fig. 1. Direct
expression of the DIII sequence (Fig. 1) was performed to
have a source of the DIII for ELISA testing after immu-
nisation of mice with AP205 VLPs carrying the DIII
sequence. Furthermore, we used highly purified and
refolded DIII protein as a congruent for immunisation of
mice in parallel with the mosaic AP205-derived VLPs.
The expression level of both AP205-am-DIII and
AP205-op-DIII polypeptides, as determined from SDS-
PAGE of total SDS-mercaptoethanol cell lysates, corre-
sponded, in general, to the suppressor capacity of the
appropriate E. coli strains (Fig. 2a). Approximately 50 %
of the total target proteins appeared in the soluble cell
fraction, similar to the separation that occurs during
expression of non-chimeric AP205 or other VLP-producing
(RNA phage Qb, hepatitis B core antigen) genes (not
shown). The non-chimeric AP205 carrier did not demon-
strate any difference in solubility in comparison to the
AP205-DIII fusions. The ratio of AP205-DIII fusions to
Mol Biotechnol
123
AP205 in the initial E. coli lysates was *50 %. During the
preparation of ultrasonicated cell lysates, a fraction of
AP205 dimers appeared and remained relatively stable
during boiling in Laemmli’s buffer; however, extensive
boiling of the final purified samples led to the disappear-
ance of the AP205 dimer band (Fig. 2b).
The mosaic VLPs yielded, on average, *8 mg of
purified AP205-DIII per gram of wet cells. After extensive
purification, the mosaic AP205-DIII VLPs demonstrated a
high purity of the target proteins (up to 90 %) with a ratio
of AP205-DIII to AP205 carrier of *0.12–0.17 to 1 within
the particles.
The minimal contamination of purified AP205-DIII
VLPs with host proteins (Fig. 2b) can be explained by
intra-particle occlusion of bacterial proteins rather than by
adherence on the VLP surface. A gradual loss of the chi-
meric AP205-DIII component of VLPs was observed dur-
ing the purification process. This gradual loss would
happen if VLPs enriched with chimeric DIII-harbouring
monomers are less stable than VLPs with a lower content
of chimeric monomers and are therefore preferentially
destroyed during purification.
Properties of Mosaic AP205 VLPs Carrying the DIII
Epitope
Double radial Ouchterlony immunoprecipitation, which
could be regarded as the most specific test for the existence
of the VLPs, demonstrated full confluence, without any
‘spurs’, of the precipitation lines formed by the AP205-am-
DIII and AP205-op-DIII VLPs with the precipitation line
produced by the non-chimeric AP205 VLPs (Fig. 2c, top).
Therefore, full ‘Ouchterlony identity’ of the AP205-
derived VLPs was demonstrated even though they differed
with respect to the presence of the AP205-DIII fusions.
Disruption of the VLPs by boiling in Laemmli’s buffer
prevented formation of the precipitation lines in the
Ouchterlony’s test (Fig. 2c, bottom).
According to electron microscopy analysis, purified
mosaic AP205-derived particles were indistinguishable
from non-purified items observed in the initial E. coli
lysates (not shown), as well as from the original AP205
carrier particles (Fig. 3).
Direct measurement of the particle size in solution using
the DLS method revealed particles with a close-to-expec-
ted diameter of 32.7 nm in the case of the control AP205,
but slightly differing diameters of 32.7 and 37.8 nm for
AP205-am-DIII and AP205-op-DIII, respectively (Fig. 4).
The DIII sequence appeared on the surface of the VLPs
because it was fully accessible to anti-DIII antibodies in a
competitive ELISA test (not shown).
The content of the encapsidated RNA within purified
mosaic AP205-DIII VLPs was estimated as 1,180 nucleo-
tides per particle; the estimated RNA content remained
constant after additional purification steps.
Double radial Ouchterlony immunodiffusion using
polyclonal rabbit anti-AP205 antibodies and NAGE con-
firmed stable association of the encapsidated RNA with the
VLPs (not shown). Therefore, we think that the residual
nucleic acids are not placed on the surface of mosaic par-
ticles, since nucleic acids are resistant to ribonuclease
treatment (not shown) and are not removed not only during
Ouchterlony immunodiffusion process, but also by DEAE
Sephadex chromatography, sucrose gradient centrifugation
or ammonium sulphate precipitation.
Properties of Regular AP205-DIII and GA-DIII
Fusions, and Purification of the Directly Expressed DIII
Protein
We were motivated to generate mosaic AP205-derived
particles because our early efforts to generate regular
Fig. 2 Monitoring of the expression and purification process of the
mosaic AP205-DIII VLP variants. a SDS-PAGE Western blot (with
polyclonal anti-AP205 antibody) of total protein in SDS-mercap-
toethanol lysed cell samples (T), supernatants of the ultrasonicated
cell lysates (S), and debris of the ultrasonicated cell lysates after
solubilisation in 7 M urea (D). b Coomassie stained SDS-PAGE of
the final purified preparations of the mosaic AP205-DIII particles,
c double radial Ouchterlony’s immunoprecipitation analysis of
AP205-DIII mosaics: native VLPs (top), VLPs boiled in Laemmli’s
buffer (bottom). The polyclonal anti-AP205 antibody was placed in
the central hole
Mol Biotechnol
123
AP205-DIII and/or GA-DIII VLPs were unsuccessful. When
regularly fused AP205-DIII or GA-DIII genes without any
intervening suppressor codons (Fig. 1) were expressed,
chimeric target proteins appeared as insoluble products
without any signs of self-assembly in bacterial cells (not
shown). The attempts to refold them in vitro, also in the
presence of the initial AP205 as a helper, failed (not shown).
Direct expression of DIII protein led to a substantial
yield, 12 mg/g of cells, of insoluble recombinant product.
The DIII protein was purified and refolded by an arginine-
mediated renaturation procedure [41], as described in the
Materials and Methods. The final yield of the renatured
product after CL4B column chromatography reached 3 mg/
g of cells. The quality of the refolded DIII protein is shown
in Fig. 2b. The purified DIII protein did not form aggre-
gates in solution and DLS analysis demonstrated particles
with a radius of 4.8 nm (Fig. 4).
Immunisation of Mice with DIII-Carrying Proteins
In Fig. 5, we present immunisation data on the AP205-op-
DIII VLPs only because analogous data on the immuni-
sation of mice with the AP205-am-DIII VLPs demonstrate
general similarities with the presented data.
The antibody response in mice against the DIII epitope
was demonstrated by direct ELISA on two different anti-
gens coated onto solid support: (i) purified DIII protein and
(ii) purified regular GA-DIII fusion, where DIII was added
C-terminally to the CP of RNA phage GA. RNA phage GA
is not cross-reactive immunologically with RNA phage
AP205. Titration on differently coated solid supports led to
the conclusion that the fused GA-DIII protein was more
Fig. 3 Electron microscopy analysis of the purified mosaic AP205-DIII VLPs. a AP205-am-DIII, b AP205-op-DIII, c AP205 VLPs as a control.
Scale bar 50 nm
Fig. 4 The size of particles in the purified samples measured by DLS
analysis. The results of the DLS size distribution are shown with the
particle radius in nm on the x-axis and the number of particles in % on
the y-axis. The arrows indicate the radius of the particles
Mol Biotechnol
123
sensitive (up to four times) as a support for anti-DIII anti-
body detection than the purified DIII polypeptide (Fig. 5a).
After immunisation of mice without any adjuvants, the
AP205-op-DIII VLPs induced an evident anti-DIII
response (Fig. 5a, top, slot 1); however, the response was
about four times weaker than the appropriate anti-AP205
carrier response (Fig. 5a, bottom, slot 1). Formulation of
the AP205-DIII VLPs in the Alhydrogel adjuvant prefer-
ably enhanced anti-DIII (Fig. 5a, top, slot 2). In all cases,
the maximal anti-DIII response was found after two boosts
on day 42 of immunisation (Fig. 5a, top).
The DIII polypeptide appears to be a weak immunogen
after immunisation of mice without any adjuvant (Fig. 5a,
top, slot 3). Formulation of the DIII polypeptide in Alhy-
drogel (Fig. 5a, top, slot 4) or silicon dioxide (Fig. 5A, top,
slot 5) enhanced the anti-DIII response to the level of the
anti-DIII response induced by the AP205-op-DIII VLPs in
Alhydrogel (Fig. 5a, top, slot 2).
Isotyping of the induced antibodies revealed a remark-
able increased ability of the AP205-op-DIII VLPs over the
DIII protein to induce anti-DIII antibodies of the IgG and,
specifically, the IgG2a isotype without any adjuvants
(Fig. 5b, top, slots 1 and 3). Without adjuvants, the DIII
polypeptide was unable to switch antibody production from
the IgM to the IgG isotype (Fig. 5b, top, slot 3). By im-
munising with adjuvants, the DIII protein acquired the
ability to perform this switch and induce IgG1 antibodies
(Fig. 5b, top, slots 4 and 5), whereas the AP205-op-DIII
VLPs demonstrated clear competence to induce anti-DIII
antibodies of both IgG1 and IgG2a/b isotypes (Fig. 5b, top,
slots 2, 4, and 5).
The AP205 carrier within the AP205-op-DIII VLPs
induced a broad spectrum of IgM, IgG1 and IgG2a/b
antibodies both in the absence and presence of the adjuvant
(Fig. 5b, bottom, slots 1 and 2).
Discussion
After the WNV-neutralising efficacy of AP205 VLPs
decorated by chemically coupled WNV DIII sequence was
shown [33], it seemed intriguing to achieve RNA phage
coat-driven VLPs carrying the DIII sequence by fusion of
the appropriate genes. Moreover, AP205-DIII fusions may
eliminate the potential uncertainty of the chemical cou-
pling [33], because the DIII sequence contains two internal
cysteine residues. Because self-assembly of the C-terminal
AP205-DIII and GA-DIII fusions in vivo and attempts to
refold them in vitro failed, construction of mosaic AP205
VLPs bearing the DIII epitope on the VLP surface was
performed in the present study.
The idea that the assembly non-competent VLP mono-
mers might be rescued into mixed or mosaic particles in the
presence of native VLP monomers as helpers was first
described for the hepatitis B virus (HBV) surface antigen
(HBsAg) [43]. By simultaneous expression of two genes,
mosaic HBsAg particles carrying poliovirus [44] and malaria
[45, 46] epitopes have been purified and successfully applied
as vaccine candidates. Interestingly, mosaic HBsAg-polio-
virus particles induced much higher titres of neutralising
antibodies to poliovirus than did the homogenous ones [44].
Additionally, mosaic V3:Ty-VLPs have been produced that
carry various V3 loops of different HIV isolates on the same
Ty particle [47]. Furthermore, incorporation of mutated VLP
Fig. 5 Immunogenicity of the DIII-carrying proteins. a Average
antibody titres to DIII (top) and AP205 carrier (bottom) for the sera
from five animals are shown. b Isotyping of the antibodies induced
against DIII (top) and AP205 carrier (bottom) after the immunisation
of mice with DIII-carrying proteins. Antibodies were diluted 1:50
with PBS
Mol Biotechnol
123
monomers into well characterised, highly symmetric icosa-
hedral VLPs has been described for the hepatitis B core
antigen (HBcAg) [48, 49]. In the case of HBcAg, the real
presence of both homo- and hetero-dimers within mosaic
particles has been documented [50].
A strategy for constructing mosaic particles was started by
introducing a linker containing translational stop codons
(UGA or UAG) between the sequences encoding a monomer
body and a foreign protein sequence, with subsequent
simultaneous synthesis of both the initial VLP monomer as a
helper moiety and a read-through fusion protein containing a
foreign sequence. This strategy was applied for RNA phage
Qb coats [51–53] and C-terminally truncated HBcAg for
exposition of hantavirus [54–56] and HBV preS [57] epitopes.
The same mosaic VLP strategy was used here in the case
of the RNA phage AP205 coats, which demonstrated def-
inite advantages as promising VLP carriers by construction
of putative prophylactic and therapeutic vaccine candidates
[36].
It is noteworthy that in the present study, both amber and
opal suppressions demonstrated similar outcomes of the
target proteins, a situation that is not always the case. For
example, the yields of analogous AP205 mosaics with Af-
fibody differed strongly between the amber and opal sup-
pression variants (Renhofa et al. personal communication).
One of the most prospective features of the mosaic
AP205 derivatives carrying the DIII epitope is their ability
to induce IgG2 antibodies, which is a result of Th1 pathway
activation. As is known for other VLP carriers, e.g. for
HBcAg VLPs, the Th1 priming and induction of IgG2
isotype antibodies correlates with the presence of encaps-
idated RNA [58, 59]. The similar Th1/Th2 switch con-
nected with the loss of encapsidated RNA has been
described for full-length and C-terminally truncated HBc
variants carrying HBV preS1 [60] and HCV [61] epitopes.
Encapsidated RNA functions in this case as a TLR-7 ligand
[62]. The cause of similar behaviour of AP205 mosaics
carrying the DIII epitope could be a subject of further
immunological studies.
Acknowledgments We wish to thank Dr. B. E. Martina for pro-
viding us with the pTrcHis2-WNV plasmid, Juris Ozols, Guntars
Zarins, Dace Priede, and Inara Akopjana for excellent technical
assistance. This work was supported by a Latvian grant 2010/0261/
2DP/2.1.1.1.0/10/APIA/VIAA/052 and FP7 Grant 261466 Vectorie.
References
1. Lim, S. M., Koraka, P., Osterhaus, A. D., & Martina, B. E.
(2011). West Nile virus: Immunity and pathogenesis. Viruses, 3,
811–828.
2. Suthar, M. S., Diamond, M. S., & Gale, M, Jr. (2013). West Nile
virus infection and immunity. Nature Reviews Microbiology, 11,
115–128.
3. Arroyo, J., Miller, C., Catalan, J., Myers, G. A., Ratterree, M. S.,
Trent, D. W., et al. (2004). ChimeriVax-West Nile virus live-
attenuated vaccine: Preclinical evaluation of safety, immunoge-
nicity, and efficacy. Journal of Virology, 78, 12497–12507.
4. Monath, T. P., Liu, J., Kanesa-Thasan, N., Myers, G. A., Nichols,
R., Deary, A., et al. (2006). A live, attenuated recombinant West
Nile virus vaccine. Proceedings of the National Academy of
Sciences United States of America, 103, 6694–6699.
5. Guy, B., Guirakhoo, F., Barban, V., Higgs, S., Monath, T. P., &
Lang, J. (2010). Preclinical and clinical development of YFV
17D-based chimeric vaccines against dengue, West Nile and
Japanese encephalitis viruses. Vaccine, 28, 632–649.
6. Dayan, G. H., Bevilacqua, J., Coleman, D., Buldo, A., & Risi, G.
(2012). Phase II, dose ranging study of the safety and immuno-
genicity of single dose West Nile vaccine in healthy adults
C50 years of age. Vaccine, 30, 6656–6664.
7. Sa E Silva, M., Ellis, A., Karaca, K., Minke, J., Nordgren, R.,
et al. (2013). Domestic goose as a model for West Nile virus
vaccine efficacy. Vaccine, 31, 1045–1050.
8. Brandler, S., Marianneau, P., Loth, P., Lacote, S., Combredet, C.,
Frenkiel, M. P., et al. (2012). Measles vaccine expressing the
secreted form of West Nile virus envelope glycoprotein induces
protective immunity in squirrel monkeys, a new model of West Nile
virus infection. Journal of Infectious Diseases, 206, 212–219.
9. Volz, A., & Sutter, G. (2013). Protective efficacy of modified
vaccinia virus Ankara in preclinical studies. Vaccine, 31,
4235–4240.
10. Pinto, A. K., Richner, J. M., Poore, E. A., Patil, P. P., Amanna, I.
J., Slifka, M. K., et al. (2013). A hydrogen peroxide-inactivated
virus vaccine elicits humoral and cellular immunity and protects
against lethal West Nile virus infection in aged mice. Journal of
Virology, 87, 1926–1936.
11. Ledgerwood, J. E., Pierson, T. C., Hubka, S. A., Desai, N.,
Rucker, S., Gordon, I. J., et al. (2011). A West Nile virus DNA
vaccine utilizing a modified promoter induces neutralizing anti-
body in younger and older healthy adults in a phase I clinical
trial. Journal of Infectious Diseases, 203, 1396–1404.
12. Roehrig, J. T. (2003). Antigenic structure of flavivirus proteins.
Advances in Virus Research, 59, 141–175.
13. Heinz, F. X., & Stiasny, K. (2012). Flaviviruses and their anti-
genic structure. Journal of Clinical Virology, 55, 289–295.
14. Wang, T., Anderson, J. F., Magnarelli, L. A., Wong, S. J., Koski,
R. A., & Fikrig, E. (2001). Immunization of mice against West
Nile virus with recombinant envelope protein. The Journal of
Immunology, 167, 5273–5277.
15. Siirin, M. T., Travassos da Rosa, A. P., Newman, P., Weeks-
Levy, C., Coller, B. A., Xiao, S. Y., et al. (2008). Evaluation of
the efficacy of a recombinant subunit West Nile vaccine in Syrian
golden hamsters. American Journal of Tropical Medicine and
Hygeine, 79, 955–962.
16. Lieberman, M. M., Nerurkar, V. R., Luo, H., Cropp, B., Carrion,
R., Jr, de la Garza, M., et al. (2009). Immunogenicity and pro-
tective efficacy of a recombinant subunit West Nile virus vaccine
in rhesus monkeys. Clinical and Vaccine Immunology, 16,
1332–1337.
17. Jarvi, S. I., Hu, D., Misajon, K., Coller, B. A., Wong, T., &
Lieberman, M. M. (2013). Vaccination of captive nene (Branta
sandvicensis) against West Nile virus using a protein-based
vaccine (WN-80E). Journal of Wildlife Diseases, 49, 152–156.
18. Metz, S. W., & Pijlman, G. P. (2011). Arbovirus vaccines;
opportunities for the baculovirus-insect cell expression system.
Journal of Invertebrate Pathology, 107, S16–S30.
19. Zhu, B., Ye, J., Lu, P., Jiang, R., Yang, X., Fu, Z. F., et al. (2012).
Induction of antigen-specific immune responses in mice by
recombinant baculovirus expressing premembrane and envelope
proteins of West Nile virus. Virology Journal, 9, 132.
Mol Biotechnol
123
20. Kanai, R., Kar, K., Anthony, K., Gould, L. H., Ledizet, M.,
Fikrig, E., et al. (2006). Crystal structure of West nile virus
envelope glycoprotein reveals viral surface epitopes. Journal of
Virology, 80, 11000–11008.
21. Lee, J. W., Chu, J. J., & Ng, M. L. (2006). Quantifying the
specific binding between West Nile virus envelope domain III
protein and the cellular receptor alphaVbeta3 integrin. Journal of
Biological Chemistry, 281, 1352–1360.
22. Beasley, D. W., & Barrett, A. D. (2002). Identification of neu-
tralizing epitopes within structural domain III of the West Nile
virus envelope protein. Journal of Virology, 76, 13097–13100.
23. Volk, D. E., Beasley, D. W., Kallick, D. A., Holbrook, M. R.,
Barrett, A. D., & Gorenstein, D. G. (2004). Solution structure and
antibody binding studies of the envelope protein domain III from
the New York strain of West Nile virus. Journal of Biological
Chemistry, 279, 38755–38761.
24. Nybakken, G. E., Oliphant, T., Johnson, S., Burke, S., Diamond,
M. S., & Fremont, D. H. (2005). Structural basis of West Nile
virus neutralization by a therapeutic antibody. Nature, 437,
764–769.
25. Choi, K. S., Nah, J. J., Ko, Y. J., Kim, Y. J., & Joo, Y. S. (2007).
The DE loop of the domain III of the envelope protein appears to
be associated with West Nile virus neutralization. Virus
Research, 123, 216–218.
26. Sanchez, M. D., Pierson, T. C., McAllister, D., Hanna, S. L.,
Puffer, B. A., Valentine, L. E., et al. (2005). Characterization of
neutralizing antibodies to West Nile virus. Virology, 336, 70–82.
27. Oliphant, T., Engle, M., Nybakken, G. E., Doane, C., Johnson, S.,
Huang, L., et al. (2005). Development of a humanized mono-
clonal antibody with therapeutic potential against West Nile
virus. Nature Medicine, 11, 522–530.
28. Chu, J. H., Chiang, C. C., & Ng, M. L. (2007). Immunization of
flavivirus West Nile recombinant envelope domain III protein
induced specific immune response and protection against West Nile
virus infection. The Journal of Immunology, 178, 2699–2705.
29. McDonald, W. F., Huleatt, J. W., Foellmer, H. G., Hewitt, D.,
Tang, J., Desai, P., et al. (2007). A West Nile virus recombinant
protein vaccine that coactivates innate and adaptive immunity.
Journal of Infectious Diseases, 195, 1607–1617.
30. Martina, B. E., Koraka, P., van den Doel, P., van Amerongen, G.,
Rimmelzwaan, G. F., & Osterhaus, A. D. (2008). Immunization
with West Nile virus envelope domain III protects mice against
lethal infection with homologous and heterologous virus. Vac-
cine, 26, 153–157.
31. Ramanathan, M. P., Kutzler, M. A., Kuo, Y. C., Yan, J., Liu, H.,
Shah, V., et al. (2009). Communication with an optimized IL15
plasmid adjuvant enhances humoral immunity via stimulating B
cells induced by genetically engineered DNA vaccines expressing
consensus JEV and WNV E DIII. Vaccine, 27, 4370–4380.
32. Martina, B. E., van den Doel, P., Koraka, P., van Amerongen, G.,
Spohn, G., Haagmans, B. L., et al. (2011). A recombinant
influenza A virus expressing domain III of West Nile virus
induces protective immune responses against influenza and West
Nile virus. PLoS One, 6, e18995.
33. Spohn, G., Jennings, G. T., Martina, B. E., Keller, I., Beck, M.,
Pumpens, P., et al. (2010). A VLP-based vaccine targeting
domain III of the West Nile virus E protein protects from lethal
infection in mice. Virology Journal, 7, 146.
34. Zeltins, A. (2013). Construction and characterization of virus-like
particles: A review. Molecular Biotechnology, 53, 92–107.
35. Pushko, P., Pumpens, P., & Grens, E. (2013). Development of
virus-like particle (VLP) technology from small highly-symmetric
to large complex VLP structures. Intervirology, 56, 141–165.
36. Tissot, A. C., Renhofa, R., Schmitz, N., Cielens, I., Meijerink, E.,
Ose, V., et al. (2010). Versatile virus-like particle carrier for
epitope based vaccines. PLoS One, 5, e9809.
37. Smiley, B. K., & Minion, F. C. (1993). Enhanced readthrough of
opal (UGA) stop codons and production of Mycoplasma pneu-
moniae P1 epitopes in Escherichia coli. Gene, 134, 33–40.
38. Raftery, L. A., Egan, J. B., Cline, S. W., & Yarus, M. (1984).
Defined set of cloned termination suppressors: In vivo activity of
isogenetic UAG, UAA, and UGA suppressor tRNAs. Journal of
Bacteriology, 158, 849–859.
39. Freivalds, J., Rumnieks, J., Ose, V., Renhofa, R., & Kazaks, A.
(2008). High-level expression and purification of bacteriophage
GA virus-like particles from yeast Saccharomyces cerevisiae and
Pichia pastoris Acta Univ. Latv. Biology, 745, 75–85.
40. Strods, A., Argule, D., Cielens, I., Jackevica, L., & Renhofa, R.
(2012). Expression of GA coat protein-derived mosaic virus-like
particles in Saccharomyces cerevisiae and packaging in vivo of
mRNAs into particles. Proceedings of the Latvian Academy of
Sciences Section B, 66, 234–241.
41. Chen, J., Liu, Y., Li, X., Wang, Y., Ding, H., Ma, G., et al.
(2009). Cooperative effects of urea and L-arginine on protein
refolding. Protein Expression and Purification, 66, 82–90.
42. Ehresmann, B., Imbault, P., & Weil, J. H. (1973). Spectropho-
tometric determination of protein concentration in cell extracts
containing tRNA’s and rRNA’s. Analytical Biochemistry, 54,
454–463.
43. Bruss, V., & Ganem, D. (1991). Mutational analysis of hepatitis
B surface antigen particle assembly and secretion. Journal of
Virology, 65, 3813–3820.
44. Delpeyroux, F., Peillon, N., Blondel, B., Crainic, R., & Streeck,
R. E. (1988). Presentation and immunogenicity of the hepatitis B
surface antigen and a poliovirus neutralization antigen on mixed
empty envelope particles. Journal of Virology, 62, 1836–1839.
45. Moelans, I. I., Cohen, J., Marchand, M., Molitor, C., de Wilde, P.,
van Pelt, J. F., et al. (1995). Induction of Plasmodium falciparum
sporozoite-neutralizing antibodies upon vaccination with recom-
binant Pfs16 vaccinia virus and/or recombinant Pfs16 protein
produced in yeast. Molecular and Biochemical Parasitology, 72,
179–192.
46. Gordon, D. M., McGovern, T. W., Krzych, U., Cohen, J. C.,
Schneider, I., LaChance, R., et al. (1995). Safety, immunoge-
nicity, and efficacy of a recombinantly produced Plasmodium
falciparum circumsporozoite protein-hepatitis B surface antigen
subunit vaccine. Journal of Infectious Diseases, 171, 1576–1585.
47. Layton, G. T., Harris, S. J., Gearing, A. J., Hill-Perkins, M., Cole,
J. S., Griffiths, J. C., et al. (1993). Induction of HIV-specific
cytotoxic T lymphocytes in vivo with hybrid HIV-1 V3:Ty-virus-
like particles. Journal of Immunology, 151, 1097–1107.
48. Loktev, V. B., Ilyichev, A. A., Eroshkin, A. M., Karpenko, L. I.,
Pokrovsky, A. G., Pereboev, A. V., et al. (1996). Design of
immunogens as components of a new generation of molecular
vaccines. Journal of Biotechnology, 44, 129–137.
49. Beterams, G., Bottcher, B., & Nassal, M. (2000). Packaging of up to
240 subunits of a 17 kDa nuclease into the interior of recombinant
hepatitis B virus capsids. FEBS Letters, 481, 169–176.
50. Kazaks, A., Dishlers, A., Pumpens, P., Ulrich, R., Kruger, D. H.,
& Meisel, H. (2003). Mosaic particles formed by wild-type HBV
core protein and its deletion variants consist of both homo- and
heterodimers. FEBS Letters, 549, 157–162.
51. Kozlovska, T. M., Cielens, I., Vasiljeva, I., Strelnikova, A.,
Kazaks, A., Dislers, A., et al. (1996). RNA phage Q beta coat
protein as a carrier for foreign epitopes. Intervirology, 39, 9–15.
52. Kozlovska, T. M., Cielens, I., Vasiljeva, I., Bundule, M., Strel-
nikova, A., Kazaks, A., et al. (1997). Display vectors. II. Recom-
binant capsid of RNA bacteriophage Qb as a display moiety.
Proceedings of the Latvian Academy of Sciences, 51, 8–12.
53. Vasiljeva, I., Kozlovska, T., Cielens, I., Strelnikova, A., Kazaks,
A., Ose, V., et al. (1998). Mosaic Qbeta coats as a new presen-
tation model. FEBS Letters, 431, 7–11.
Mol Biotechnol
123
54. Koletzki, D., Zankl, A., Gelderblom, H. R., Meisel, H., Dislers,
A., Borisova, G., et al. (1997). Mosaic hepatitis B virus core
particles allow insertion of extended foreign protein segments.
Journal of General Virology, 78, 2049–2053.
55. Ulrich, R., Koletzki, D., Lachmann, S., Lundkvist, A., Zankl, A.,
Kazaks, A., et al. (1999). New chimaeric hepatitis B virus core
particles carrying hantavirus (serotype Puumala) epitopes:
Immunogenicity and protection against virus challenge. Journal
of Biotechnology, 73, 141–153.
56. Kazaks, A., Lachmann, S., Koletzki, D., Petrovskis, I., Dislers,
A., Ose, V., et al. (2002). Stop-codon insertion restores the par-
ticle formation ability of hepatitis B virus core-hantavirus
nucleocapsid protein fusions. Intervirology, 45, 340–349.
57. Kazaks, A., Borisova, G., Cvetkova, S., Kovalevska, L., Ose, V.,
Sominskaya, I., et al. (2004). Mosaic hepatitis B virus core par-
ticles presenting the complete preS sequence of the viral envelope
on their surface. Journal of General Virology, 85, 2665–2670.
58. Riedl, P., Stober, D., Oehninger, C., Melber, K., Reimann, J., &
Schirmbeck, R. (2002). Priming Th1 immunity to viral core
particles is facilitated by trace amounts of RNA bound to its
arginine-rich domain. Journal of Immunology, 168, 4951–4959.
59. Sominskaya, I., Skrastina, D., Petrovskis, I., Dishlers, A., Berza,
I., Mihailova, M., et al. (2013). A VLP library of C-terminally
truncated hepatitis B core proteins: Correlation of RNA encaps-
idation with a Th1/Th2 switch in the immune responses of mice.
PLoS One, 8, e75938.
60. Skrastina, D., Bulavaite, A., Sominskaya, I., Kovalevska, L., Ose,
V., Priede, D., et al. (2008). High immunogenicity of a hydro-
philic component of the hepatitis B virus preS1 sequence exposed
on the surface of three virus-like particle carriers. Vaccine, 26,
1972–1981.
61. Sominskaya, I., Skrastina, D., Dislers, A., Vasiljev, D., Mihail-
ova, M., Ose, V., et al. (2010). Construction and immunological
evaluation of multivalent hepatitis B virus (HBV) core virus-like
particles carrying HBV and HCV epitopes. Clinical and Vaccine
Immunology, 17, 1027–1033.
62. Lee, B. O., Tucker, A., Frelin, L., Sallberg, M., Jones, J., Peters, C.,
et al. (2009). Interaction of the hepatitis B core antigen and the
innate immune system. Journal of Immunology, 182, 6670–6681.
Mol Biotechnol
123